The Scientific World Journal

Volume 2014 (2014), Article ID 480732, 10 pages

http://dx.doi.org/10.1155/2014/480732

Research Article

The Effectiveness of Anti-R. equi Hyperimmune Plasma against R. equi Challenge in Thoroughbred Arabian Foals of Mares Vaccinated with R. equi Vaccine

Osman Erganis,¹ Zafer Sayin,¹ Hasan Huseyin Hadimli,¹ Asli Sakmanoglu,¹ Yasemin Pinarkara,² Ozgur Ozdemir,³ and Mehmet Maden⁴

¹Department of Microbiology, Faculty of Veterinary Medicine, University of Selcuk, 42075 Konya, Turkey

²Program of Food Technology, Sarayonu Vocational School, University of Selcuk, 42075 Konya, Turkey

³Department of Pathology, Faculty of Veterinary Medicine, University of Selcuk, 42075 Konya, Turkey

⁴Department of Internal Medicine, Faculty of Veterinary Medicine, University of Selcuk, 42075 Konya, Turkey

Received 3 December 2013; Accepted 5 March 2014; Published 3 April 2014

Academic Editors: T. Betakova, V. Fedorenko, Y. Mu, Z. Shi, and H. Zaraket

Copyright © 2014 Osman Erganis et al. This is an open access article distributed under the Creative Commons Attribution License, which permits unrestricted use, distribution, and reproduction in any medium, provided the original work is properly cited.

Abstract.

This study aimed to determine the effectiveness of a pregnant mare immunization of a Rhodococcus equi (R. equi) vaccine candidate containing a water-based nanoparticle mineral oil adjuvanted (Montanide IMS 3012) inactive bacterin and virulence-associated protein A (VapA), as well as the administration of anti-R. equi hyperimmune (HI) plasma against R. equi challenge in the mares’ foals. The efficacy of passive immunizations (colostral passive immunity by mare vaccination and artificial passive immunity by HI plasma administration) was evaluated based on clinical signs, complete blood count, blood gas analysis, serological response (ELISA), interleukin-4 (IL-4) and interferon gamma (IFN-γ), total cell count of the bronchoalveolar lavage fluids (BALF) samples, reisolation rate of R. equi from BALF samples (CFU/mL), lung samples (CFU/gr), and lesion scores of the organs and tissue according to pathological findings after necropsy in the foals. The vaccination of pregnant mares and HI plasma administration in the foals reduced the severity of R. equi pneumonia and lesion scores of the organs and tissue by 3.54-fold compared to the control foals. This study thus indicates that immunization of pregnant mares with R. equi vaccine candidate and administration of HI plasma in mares’ foals effectively protect foals against R. equi challenge.

1. Introduction

Rhodococcus equi (R. equi) is a Gram-positive, nonmotile, obligate aerobe, intracellular microorganism. Virulent R. equi causes pyogranulomatous bronchopneumonia in young foals aged from 1 to 6 months [1]. Young foals may also develop extrapulmonary disease, such as septic arthritis, osteomyelitis, ulcerative enterocolitis, mesenteric lymphadenopathy, neonatal diarrhea, and sudden death. R. equi is additionally considered as an opportunistic pathogen of immunosuppressed people, especially AIDS patients [2]. R. equi was initially isolated from pulmonary lesions of foals by Magnusson in 1923 [3]. R. equi bacterium is present in soil and horse feces. Foals are thought to become infected when, within the first few days of life, they ingest or breathe in soil, dust, or fecal particles harboring the bacteria [2, 4]. Inhalation of aerosolized virulent R. equi from the environment and intracellular replication within alveolar macrophages is essential components of pathogenesis of R. equi pneumonia in foals [5]. Virulence in foals is associated with the presence of 80–90 kb plasmids that encode the 15–17 kDa lipoprotein “virulence-associated protein A” (VapA) [6]. The disease is endemic on some farms and sporadic on other farms, but nonexistent on most farms. Recent epidemiologic studies indicate that the difference in the disease’s prevalence on farms directly relates to differences in foal population density, farm management, and environmental factors, such as temperature, dust, soil pH, and the number of virulent R. equi organisms in the soil [7].

Several antimicrobial agents are active against R. equi in vitro. However, since R. equi is a facultative intracellular pathogen that survives, replicates in macrophages, and causes pyogranulomatous lesions, many of these agents are ineffective in vivo [8]. R. equi pneumonia significantly impacts the equine industry by posing financial losses since foals that recover from the disease are less likely to race as adults. The cost of therapy and occasional death of foals also pose financial risks. Furthermore, treatment with long-term antibiotics does not guarantee full recovery [9].

Due to the epitheliochorial placentation of equines, foals must obtain all maternally derived antibodies from the ingestion of colostrum [10]. Ingestion of colostrum from hyperimmunized mares was found to be associated with protection against R. equi in foals normally hypogammaglobulinemic at birth [11, 12]. Foals become infected approximately when maternal antibody concentrations wane [13]. Immunization of mares has been suggested by several researchers to prevent R. equi infection in foals [11, 12, 14–17]. Traditional hyperimmune plasma therapy is currently the only proven method for prevention of R. equi in foals, especially those exhibiting passive antibody transfer failure [11, 12, 15].

Due to the presence of the maternal antibody and the immaturity of foals’ immune system, vaccination of neonate presents different results [18–20], yet none of the control strategies to protect horses from R. equi infection have proven successful. Several vaccines have been investigated for the prevention of R. equi, though none have been developed for widespread vaccination [21].

This study thus aimed to determine the effectiveness of a pregnant mare immunization with a R. equi vaccine candidate and the administration of anti-R. equi hyperimmune plasma against R. equi challenge in these mares’ foals.

2. Materials and Methods

2.1. Immunization of Mares

Four pregnant thoroughbred Arabian mares were vaccinated three times at months 8, 9, and 10 during pregnancy. Vaccination was performed intramuscularly with the R. equi vaccine candidate containing a water-based nanoparticle mineral oil adjuvanted (IMS 3012, SEPPIC, Paris, France) inactive antigen and VapA. Four mares not vaccinated formed the control group. Serum samples were collected from each mare at birth to test the presence of an anti-R. equi-specific antibody by ELISA. ELISA was carried out according to Takai et al. [22].

Nine healthy Arabian mares were selected for the production of anti-R. equi hyperimmune plasma. After proving to be free of equine infectious anemia (EIA), dourine, glanders, African horse sickness, and S. abortus equi, the mares were hyperimmunized 5 days apart with four doses of inactive R. equi. After 10 to 15 days, mares were vaccinated 21 days apart with 3 doses of R. equi vaccine candidate [23, 24]. After 15 to 20 days following the most previous immunization, serum samples were obtained from the mares and tested by ELISA for anti-R. equi antibody titers [22]. Horses having anti-R. equi antibody titers ≥1/12800 by ELISA were selected as plasma donors. Donor horses were bled, and the hyperimmune plasma was separated from the blood cells by plasmapheresis (PCS2, Haemonetics, Braintree, MA, USA). The plasma samples were packed in 200 mL sterile bottles in a BSL 2 cabinet and stored at 4°C. Sterility tests for aerobic, anaerobic bacteria, mycoplasma, and mycotic agents as well as mouse safety tests were performed, after which the hyperimmune plasma samples were used. Donor horses were subsequently vaccinated at intervals of 50 to 60 days and tested 10 to 15 days later, and if the titers were again satisfactory, they were again bled.

2.2. Challenge

To determine the effectiveness of a pregnant mare immunization using a R. equi vaccine candidate and HI plasma activity against R. equi infection in foals, 4 weeks old mares which born four vaccinated and four unvaccinated mares challenged the 2 mL of CFU pathogen R. equi by intercostal injection in the lobe of the left lung [25, 26]. Before receiving the challenge, foals were kept together with their dams approximately 3 weeks after birth to ingest a sufficient amount of colostrum. Two days before the challenge, 150 mL of HI plasma was administered to each foal of the vaccinated mares by intravenous infusion and 50 mL by subcutaneous infusion at days 1, 5, 9, 13, and 17 after the challenge. HI plasma was not given to the foals of unvaccinated mares.

2.3. Laboratory Tests

Blood samples were obtained from the challenged foals to determine the presence of anti-R. equi specific antibodies using a ELISA on the challenge day (day 0) and on days 10 and 20, to measure the interleukin-4 (IL-4) and interferon gamma (IFN-γ) concentrations on days 0, 1, 10, 20, and 30 and for complete blood count and blood gas analysis on days 0, 1, 5, 10, 14, 20, and 30 [25]. BALF samples were taken by passing a nasotracheal tube and in fusing 20 mL of sterile saline solution to bacterial culture and measure total cell count (TCC) on days 0, 1, 5, 10, 14, 20, and 30 [25, 26]. BALF samples were collected according to the method described by Mansmann and Knight [27] and Higuchi et al. [28]. The IL-4 and IFN-γ levels were measured using the Horse IL-4 ELISA kit (product code CSB-E14223Hs [96 T], Cusabio, Wuhan, Hubei, China) and Equine IFN-γ ELISA kit (ALP) (product code 3117-1A-6, MabTech, Thomastown, VIC, Australia) according to the manufacturer’s instructions. The optimal dilutions of the serum samples, conjugate, substrate, and concentration of the coating antigen were standardized in our laboratory.

2.4. Clinical Examination

Fever (F), respiratory rate (R), pulse rate (P), cough, bronchial sounds, nasal discharge, and mucous membranes of foals were examined on days 0, 1, 5, 10, 14, 20, and 30. Clinical and respiratory system signs were defined as regular (0), mild (1), moderate (2), and severe (3) and normal (0), congested (1), and cyanotic (2) for mucous membranes.

2.5. Postmortem Examination

Foals were euthanized with an intravenous injection of a mixture of 100 mg of suxamethonium chloride and 22.5 mg sodium chloride (Lysthenon 2%, Fako, Turkey) 30 days after the challenge, and necropsy was performed. Macroscopic lesions in lungs and organs were scored according to Table 1.

Table 1: Macroscopic lesions scores in lungs and organs after necropsy.

Postmortem Lesion Scores

Organs
No lesion (0)
Mild (1)
Moderate (2)
Severe (3)
Very severe (4)

Lung
Without lesions
With 2 to 3 small pyogranulomas or large abscess formation limited to only one lobe of the lung and focal consolidation
With four to five pyogranulomas limited to two lobes of the lung multifocal consolidation and large abscess formation
With a large number of differently sized pyogranulomas limited to three lobes or between the right and left lobes of the lung
With military or differently sized pyogranulomas spread over all lobes of the lung

Lymph 

node
Without lesions
With slight growth
With mild growth
Overgrown and with limited pus foci of the cross-sectional surface
Overgrown and purulent

Heart
Without lesions
With slight paleness
With a wide area of paleness in the epicardium and endocardium or pyogranuloma
With a wide area of paleness in the cross-sectional area or a few pyogranulomas
With a wide area of paleness in the cross-sectional area or several pyogranulomas

Liver
Without lesions
Slightly enlarged and congested
Enlarged and mottled appearance or with pyogranuloma
With numerous pyogranulomas in the cross-sectional area and under the capsule
With pyogranulomas spread over the entire surface and the cross-sectional area

Kidney
Without lesions
Slightly enlarged
Enlarged kidneys and mottled appearance
Enlarged kidneys and with pyogranuloma in the cross-sectional area and infarction area
Enlarged kidneys and with numerous pyogranulomas in the cross-sectional area and infarction area

Spleen
Without lesions
Slightly enlarged
Overgrown and with pyogranuloma in the cross-sectional area
Overgrown and with a few pyogranulomas in the cross-sectional area
Overgrown and with numerous pyogranulomas in the cross-sectional area

Samples from these organs were fixed in 10% formalin and embedded in paraffin wax blocks. Block sections of 5 µm thickness were stained with Luna [29]. All sections were evaluated under a light microscope.

2.6. Statistical Analysis

All statistical analyses were performed using the Student’s -test.

3. Results

Two foals (numbers 5 and 7) of unvaccinated mares died before the challenge, and R. equi, Streptococcus sp., and Corynebacterium sp. were isolated from the lungs of these dead foals. In the place of the dead foals, two unvaccinated mares’ foals were included in the study. One of these foals died on day 7 and another on day 13 after the challenge.

Anti-R. equi antibody titer measured in vaccinated mares was higher than in the unvaccinated mares at birth by ELISA. In the foals of vaccinated mares, anti-R. equi antibody titer was determined to be 1/1600 of the maximum after the administration of hyperimmune plasma, and 1/200 titer was also determined in control foals (Table 2).

Table 2: Anti-R. equi antibody ELISA titer of vaccinated and unvaccinated mares and challenged foals.

Mare group
Mare number
ELISA titer at birth
Foal group
Foal number
ELISA titer after challenge

Day 0
Day 10
Day 20

Vaccinated
1
1/12800
Vaccine + HI plasma
1
1/800
1/1600
1/1600

2
1/6400
2
1/100
1/400
1/800

3
1/3200
3
1/800
1/1600
1/1600

4
1/6400
4
1/400
1/800
1/800

Unvaccinated
5
Negative
Control
5
0
1/200
*

6
1/200
6
0
Negative
1/200

7
Negative
7
0
*
*

8
Negative

8
0
Negative
1/200

Because foals died, ELISA titer was not measured on these days.

The IL-4 concentration was measured to have a mean of <16 pg/mL at days 0, 10, and 20 and a mean of 80 pg/mL at day 30 in foals of the vaccinated group, as well as a mean of 32 pg/mL in control foals. IFN-γ concentration increased on day 10 compared to the challenge day in both vaccine and control groups. By day 20, the control group remained stable, while the vaccine group exhibited doubling. By day 30, it increased in both groups but was measured to be 4.1-fold more in the vaccine group than in the control group (Table 3).

Table 3: IL-4 (pg/mL) and IFN-γ (ng/mL) concentration in challenged foals.

Foal group
Foal number
Day 0
Day 10
Day 20
Day 30

IL-4/IFN-γ
IL-4/IFN-γ
IL-4/IFN-γ
IL-4/IFN-γ

Vaccine + HI plasma
1
<16/<0.01
<16/0.01
<16/0.02
128/0.05

2
<16/<0.005
<16/0.005
<16/0.01
128/0.05

3
<16/<0.005
<16/0.005
<16/0.01
32/0.05

4
<16/<0.005
<16/0.005
<16/0.01
32/0.05

Mean
<16/<0.0075
<16/0.0075
<16/0.015
80/0.05

Control
5
<16/<0.005
<16/0.005
*
*

6
<16/<0.005
<16/0.005
<16/0.001
32/0.005

7
<16/<0.005
*
*
*

8
<16/<0.005
<16/0.005
<16/0.01
32/0.02

Mean
<16/<0.005
<16/0.005
<16/0.0055
32/0.012

Because the foals died, IL-4 and IFN-γ concentration were not measured on these days.

The reisolation rate of R. equi from BALF samples was determined to have increased by day 10, decreased by day 20, and increased again by day 30 in the vaccinated and HI plasma-administered group. An increase was observed in the control group compared to day 1 (Table 4, Figure 1).

Table 4: Reisolation rate of R. equi from BALF samples (CFU/mL) and lung samples (CFU/gr) after necropsy in foals.

Foal group
Foal number
Day 0
Day 1
Day 10
Day 20
Day 30
Necropsy

Vaccine + HI plasma
1
0
65000
135
1400
140
50

2
0
1000
55
1220
0
21000

3
0
1300
120
12700
0
0

4
0
2600
195
90000
170000
**

Mean
0
17475
126
26330
42535

Control
5
0
19000
800
died
—
**

6
0
4100
3600
1300000
1100000
320000

7
0
5500
Died
—
—
**

8
0
83000
640000
2300
100000
3250000

Mean
0
27900
214666
651150
600000

Too many to count.

Figure 1: Reisolation rate of R. equi from foals’ BALF samples (CFU/mL).

A decrease in the concentration of pO2 and SO2 in the vaccine group was observed on day 5. The concentration of pCO2 and tCO2 increased, while the concentration of SO2 decreased on day 10. A decrease in the concentration of pO2 and SO2 in the control group was observed on day 30 () (Table 6).

An insignificant () increase was observed in WBC concentration in both the control and vaccine group during the study period. Significant () differences were determined in percentages of LYM, MON, and GRAN concentration. The RBC concentration decreased significantly () on days 14 and 30 (Table 6).

TCC of BALF and lung scores had increased in both groups by day 14 (Table 5). These increases were statistically significant () in the control group, yet insignificant () in the vaccine group.

Table 5: Total cell count (TCC) of BALF samples, clinical signs, respiratory system signs, mucous membrane scores, and temperature of foals.

Foal group
Day 0
Day 1
Day 5
Day 10
Day 14
Day 20
Day 30

BALF-TCC
Control
300.00 ± 57.74
300.00 ± 57.74
300.00 ± 57.74
300.00 ± 57.74
466.67 ± 266.67
8800.00 ± 8400.00
1500.00 ± 1100.00

Vaccinated
300.00 ± 57.74
300.00 ± 57.74
300.00 ± 57.74
300.00 ± 57.74
2600.00 ± 1116.54
1000.00 ± 258.20
1950.00 ± 1040.43

Clinical score
Control
0.00 ± 0.00
0.00 ± 0.00
0.00 ± 0.00
0.00 ± 0.00
1.00 ± 1.00
0.00 ± 0.00
0.00 ± 0.00

Vaccinated
0.00 ± 0.00
0.00 ± 0.00
0.00 ± 0.00
0.00 ± 0.00
0.00 ± 0.00
0.00 ± 0.00
0.00 ± 0.00

Respiratory system score
Control
0.00 ± 0.00
0.00 ± 0.00
0.00 ± 0.00 B
1.00 ± 0.58
0.67 ± 0.33 B
0.00 ± 0.00 B
0.00 ± 0.00 B

Vaccinated
1.00 ± 0.00
0.00 ± 0.00
1.25 ± 0.48 A
2.00 ± 0.00
0.275 ± 0.25 A
2.75 ± 0.25 A
2.75 ± 0.25 A

Mucous

membrane score
Control
0.00 ± 0.00
0.00 ± 0.00
0.00 ± 0.00
0.00 ± 0.00
0.33 ± 0.33
0.00 ± 0.00
0.00 ± 0.00

Vaccinated
0.00 ± 0.00
0.00 ± 0.00
0.00 ± 0.00
0.00 ± 0.00
0.00 ± 0.00
0.00 ± 0.00
0.00 ± 0.00

Temperature
Control
38.3 ± 0.12
38.43 ± 0.11
38.05 ± 0.23
27.90 ± 9.31
37.87 ± 0.24
38.20 ± 0.20
38.45 ± 0.05

Vaccinated
38.13 ± 0.13
38.33 ± 0.22
38.50 ± 0.11
38.45 ± 0.06
38.05 ± 0.16
38.60 ± 0.07
38.60 ± 0.07

Table 6: Complete blood count and blood gas analysis results of foals.

Foal group
Day 0
Day 1
Day 5
Day 10
Day 14
Day 20
Day 30

pH (7.34–7.43)
Control
7.45 ± 0.02
7.41 ± 0.02
7.43 ± 0.02
7.35 ± 0.03
7.42 ± 0.01
7.45 ± 0.02
7.40 ± 0.02

Vaccinated
7.43 ± 0.01
7.42 ± 0.01
7.41 ± 0.01
7.41 ± 0.01
7.41 ± 0.01
7.39 ± 0.01
7.42 ± 0.01

pCO2 (38–48 mmHg)
Control
37.50 ± 1.19
42.25 ± 0.75
45.75 ± 1.93
52.75 ± 2.78 A
47.33 ± 2.73
40.50 ± 1.50
47.00 ± 3.00

Vaccinated
40.00 ± 1.78
42.00 ± 1.47
42.00 ± 0.41
40.25 ± 125 B
42.00 ± 2.74
45.00 ± 3.14
40.50 ± 1.26

pO2 (37–56 mmHg)
Control
35.00 ± 2.12
35.00 ± 2.12
36.75 ± 1.55 A
33.00 ± 1.35
32.00 ± 2.08
38.00 ± 4.00
34.00 ± 1.01 B

Vaccinated
37.25 ± 3.71
33.50 ± 2.63
29.00 ± 1.91 B
36.25 ± 1.75
53.75 ± 21.46
33.75 ± 2.29
41.25 ± 1.38A

tCO2
Control
26.98 ± 1.26
28.03 ± 1.21
31.53 ± 1.81
30.53 ± 0.61 A
31.87 ± 1.18
29.05 ± 0.55
30.20 ± 0.90

Vaccinated
27.85 ± 0.45
28.35 ± 0.73
28.05 ± 0.29
26.75 ± 0.84 B
27.95 ± 1.47
54.15 ± 27.30
27.65 ± 0.57

SO2 (>60 mmHg)
Control
70.00 ± 2.48
67.00 ± 3.37
71.50 ± 1.32 A
71.50 ± 1.32 A
62.67 ± 4.67
74.50 ± 4.50
65.00 ± 1.00 B

Vaccinated
71.25 ± 6.70
64.75 ± 4.87
55.50 ± 4.29 B
55.50 ± 4.29 B
71.50 ± 9.50
53.90 ± 7.42
77.75 ± 1.38 A

WBC (5–12 × )
Control
7.08 ± 1.01
7.68 ± 1.31
7.32 ± 1.16
7.02 ± 1.12
5.65 ± 1.66
4.64 ± 0.37
10.53 ± 2.61

Vaccinated
6.66 ± 0.87
5.86 ± 0.33
8.82 ± 1.29
8.86 ± 0.87
8.60 ± 0.66
26.90 ± 15.77
10.33 ± 1.57

LYM (% 20–40)
Control
15.60 ± 2.46 B
15.70 ± 0.90 B
22.65 ± 2.41
22.80 ± 1.86 B
29.13 ± 11.52
36.85 ± 14.75
17.50 ± 10.00

Vaccinated
35.60 ± 3.98 A
30.65 ± 2.23 A
34.63 ± 6.43
36.75 ± 4.88 A
37.83 ± 4.26
27.11 ± 6.51
31.85 ± 3.40

MON (% 2–8)
Control
1.40 ± 0.12 B
1.68 ± 0.11
3.55 ± 0.13
3.43 ± 0.77
3.67 ± 1.22
3.50 ± 0.90
1.60 ± 0.70 A

Vaccinated
2.75 ± 0.45 A
2.73 ± 0.52
3.00 ± 0.48
3.05 ± 0.46
3.58 ± 0.33
8.00 ± 5.90
2.53 ± 0.46

GRAN (% 50–70)
Control
83.00 ± 2.55 A
82.63 ± 0.92 A
73.80 ± 2.46
73.78 ± 2.32
67.20 ± 12.72
59.65 ± 15.65
80.90 ± 10.70

Vaccinated
61.65 ± 3.70 B
64.75 ± 4.87 B
62.38 ± 6.69
60.20 ± 5.10
58.60 ± 4.42
49.43 ± 16.35
65.63 ± 3.78

RBC (7–13 × )
Control
8.87 ± 0.48
9.28 ± 0.89
9.27 ± 0.39
9.10 ± 0.71
8.10 ± 0.64 B
9.01 ± 1.16
8.05 ± 0.24 B

Vaccinated
9.65 ± 0.32
11.30 ± 1.02
10.22 ± 0.34
10.03 ± 0.22
9.89 ± 0.26 A
25.16 ± 15.82
9.98 ± 0.27 A

MCV (35–60 fl)
Control
32.63 ± 0.29 A
32.83 ± 0.24 A
32.78 ± 0.71 A
34.48 ± 0.47 A
33.23 ± 0.91
32.70 ± 0.90
32.00 ± 1.90

Vaccinated
29.43 ± 1.14 B
29.95 ± 0.76 B
29.50 ± 0.93 B
29.30 ± 0.99 B
30.85 ± 0.92
26.24 ± 5.43
30.50 ± 0.68

HCT (% 32–53)
Control
28.85 ± 1.39
30.43 ± 3.04
30.30 ± 1.10
31.38 ± 2.66
26.77 ± 1.39
29.30 ± 3.00
25.65 ± 0.75 B

Vaccinated
28.43 ± 1.98
33.70 ± 2.90
30.10 ± 1.11
29.35 ± 1.42
30.43 ± 0.92
29.18 ± 0.71
30.33 ± 0.50 A

MCHC (30–42 g/dL)
Control
39.75 ± 0.43
36.18 ± 2.50
39.63 ± 0.26
36.78 ± 0.86
37.43 ± 0.45
38.85 ± 0.15
40.50 ± 1.20

Vaccinated
39.50 ± 1.67
40.60 ± 0.94
43.65 ± 3.07
41.73 ± 1.15
37.93 ± 0.61
38.40 ± 0.93
38.70 ± 1.09

RDW (8–12)
Control
14.45 ± 0.10
14.60 ± 0.47 B
14.30 ± 0.27 B
14.10 ± 0.43 B
14.13 ± 0.29
15.05 ± 0.85
16.65 ± 0.65

Vaccinated
15.40 ± 0.54
16.00 ± 0.31 A
15.85 ± 0.37 A
16.18 ± 0.55 A
16.30 ± 0.83
16.70 ± 1.00
17.15 ± 0.84

HB (11–17 g/dL)
Control
11.48 ± 0.47
10.83 ± 0.59
12.03 ± 0.51
11.53 ± 0.86
10.03 ± 0.64
11.40 ± 1.20
10.40 ± 0.00

Vaccinated
11.18 ± 0.55
13.68 ± 1.12
12.40 ± 0.44
12.23 ± 0.43
11.55 ± 0.39
11.23 ± 0.44
11.75 ± 0.48

THR (100–400 m/mm³)
Control
278.50 ± 87.36
330.50 ± 87.36
287.00 ± 44.53
238.50 ± 29.83 B
171.33 ± 30.69
240.00 ± 37.00
241.50 ± 8.50

Vaccinated
248.50 ± 30.01
317.00 ± 40.26
410.00 ± 49.83
384.50 ± 9.56 A
244.00 ± 19.20
341.50 ± 26.38
279.00 ± 25.65

The clinical and lung auscultation findings indicate that clinical signs commenced on day 5 and increased until day 10 in both groups. In the vaccine group, however, it began to decrease after day 10 and because of the sepsis two foals died on days 7 and 15 in the control group.

The mean of total lesion scores of the organs and tissue was determined to be 78 in control group and 22 in the vaccine group. According to pathological findings, the severity of R. equi pneumonia and lesion scores of the organs and tissue was observed 3.54-fold less in the vaccinated and HI plasma-administered foals compared to the control foals (Table 7, Figure 2).

Table 7: Lesion scores of the organs and tissue according to pathological findings.

Foal group
Foals number
Lung
Bronchial LN
Mediastinal LN
Heart
Liver
Kidney
Spleen
Cecum LN
Total foal score
Total group score
Mean group score

Vaccine + HI plasma
1
1
1
0
0
0
0
0
2
4
    22
    5.5

2
0
2
2
0
0
0
1
1
6

3
1
1
1
0
0
0
0
0
3

4
3
3
2
0
0
0
0
1
9

Control
5
4
4
4
4
4
4
4
4
32
    78
    19.5

6
3
1
1
2
0
0
0
1
8

7
4
4
4
4
4
4
4
4
32

8
3
1
1
0
0
0
0
1
6

Figure 2: (a) Normal lung in a foal of vaccine group, (b) pyogranuloma formation in the R. equi inoculated left lung of a control foal (arrow), (c) pyogranuloma in lung, and (d) infarction areas in kidney of control foals (arrows).

4. Discussion

Cell-mediated immunity is thought to play an important role in eliminating the facultative intracellular pathogen from foals, yet humoral immunity seems to be critically involved in the early protection in young foals. Foals are the most susceptible to the effects of virulent organisms when maternal antibody levels wane [30, 31]. The passive transfer of immunity plays a critical role in the foals’ resistance to a variety of infectious agents. Due to the epitheliochorial placentation of equines, foals must obtain all of their maternally derived antibodies by ingesting colostrum [10]. The lowest circulating antibody titers in foals appear from 1 to 6 months via the combined effects of waning maternally derived antibodies and low endogenous antibody production [32]. As a result, foals are susceptible to R. equi pneumonia during this period. Due to age-dependent susceptibility to R. equi, foals need to develop anti-R. equi immunity shortly after birth [25].

Since R. equi lives within macrophages, it resists many common antibiotics, and antibiotics-based therapy is prolonged, expensive, possibly associated with adverse effects, and inconsistently successful [33].

Studies investigating the active immunization of mares as a means of enhancing the passive transfer of virulent R. equi antibodies in colostrum and protecting foals from R. equi pneumonia have yielded mixed results. Solo vaccination of mares has not proven protective against R. equi pneumonia in foals, despite a significant increase in a colostral-specific antibody [14, 34]. Martens et al. [34], Madigan et al. [35], and Varga et al. [36] did not observe protection in foals against R. equi pneumonia after mare vaccination. Moreover, Hines et al. [31] reported that immunoglobulin in mares may not be efficiently transferred via colostrum. However, according to other researchers, passive antibody transfer from ingested colostrum was found to be associated with protection against R. equi in foals normally hypogammaglobulinemic at birth [11, 12, 14, 15]. Immunization of pregnant mares with virulent R. equi and VapA protein antigen associated with a water-based nanoparticle adjuvant as a candidate vaccine developed a higher serum IgG and opsonic activity, which resulted in passive antibody-mediated protection of foals [14]. Muscatello [17] reported that the protective effect was associated with an increase in the opsonic capacity of polymorphonuclear leucocytes against virulent R. equi in foals from immunized mares.

Martens et al. [37] were the first to show the immunoprophylactic capacity of specific hyperimmune plasma in an experimental model of R. equi pneumonia in foals. Other researchers have reported a reduction in foal morbidity and mortality due to R. equi as a result of HI plasma administration [14, 35, 37–39]. However, several other studies report no protective effects of HI plasma [11, 12, 40].

According to our results, the immunization of pregnant mares with a R. equi vaccine candidate and the administration of the anti-R. equi HI plasma in vaccinated mares’ foals proved to have protective effects during experimental R. equi infection. The clinical signs of pneumonia were significantly delayed, and the reisolation rate of R. equi from BALF samples decreased. The natural mortality rate due to R. equi infection was less than 50% in these foals compared to the controls. The severity of R. equi pneumonia and lesion scores of the organs and tissue determined 3.54-fold less than control foals.

The protective components of HI plasma are not completely known. Antibodies to Vap proteins, specifically VapA, appear to be crucially important [17]. It has been reported that there is no correlation between the total serum IgG levels and concentration of the specific anti-R. equi antibody [34, 35]. The phagocytic ability of foal neutrophils has been found comparable to adults, but the lymphocyte stimulation response alone did not influence the course of R. equi infection, while the opsonic ability of foal serum was found to be a limited factor for phagocytosis from the ages of 1 to 6 weeks [41, 42]. Phagocytic activity of foal neutrophils was found to improve when mixed with adult serum or plasma [43], which may be related to unknown, nonspecific immune factors provided by HI plasma and normal adult equine plasma that are absent from colostrum, such as fibronectin, complement, and cytokines [12, 40, 44]. The effectiveness of HI plasma is likely to be affected by the dosage, timing of administration, innate immune system competence, management conditions, and number of virulent bacterin in the environment [45].

Cytokines IFN-γ and IL-4 are major macrophage and neutrophil-activating factors, as well as upregulated microbial killing pathways [46]. It is reported that newborn foals had a deficiency of IFN-γ/IL-4 and levels not reaching adult status until approximately 4 months of age [47]. Reduced IFN-γ and IL-4 expression have a limited killing capacity of phagocytes in young foals [47, 48]. In our study, the IFN-γ and IL-4 concentration measured 4.1-fold and 2.5-fold more in the foals of vaccinated mares and HI plasma-administered, respectively, compared to the control foals.

According to changes in blood gases of foals, it was observed that lung ventilation in the challenge group had been affected by day 5, intensified after day 10, and continued to increase during the study period.

The important decrease () of the RBC concentration on days 14 and 30 and significant differences () of the MCV and RDW values in the vaccine and control group were evaluated as microcytic/normocytic-normochromic-regenerative anemia which was interpreted as a response to emerging infectious.

Given the decrease in the number in the controls, BALF-TCC parameters were detected as statistically insignificant ().

According to clinical scores and laboratory findings, the effect of infection in the vaccine group began on day 5, increased from day 9 to 14, and was constant from days 20 to 30. The effect of infection was similar in the control group, though the clinical findings increased from days 7 to 15, and two foals died of sepsis during this latter period. These findings show that resistance to infection was low in the control group.

As yet there is no licensed vaccine for the prevention of R. equi. However, on January 27, 2011, Intervet/Schering-Plough Animal Health announced that a vaccine against Rhodococcus equi infection in foals had entered the final stages of development [49].

5. Conclusions

Our results indicate that the immunization of pregnant mares with a water-based nanoparticle mineral oil adjuvanted (IMS 3012) inactive bacterin and VapA and the administration of HI plasma in foals of these mares effectively protect foals against R. equi challenge. Foals are born into the R. equi contaminated environment due to mares carrying the R. equi in their intestines. R. equi infection can be controlled by both the mares’ vaccination and anti-R. equi-HI plasma administration in foals of such dams.

Conflict of Interests

The authors declare that there is no conflict of interests regarding the publication of this paper.

Acknowledgments

This study was supported by the Scientific and Technological Research Council of Turkey (Project no. 108 G 030). This research has been approved (date 15/02/2008 and 2008/010) by the Ethics Committee of the Faculty of Veterinary Medicine at the University of Selcuk in Konya, Turkey.

References

J. F. Prescott, “Epidomiology of Rhodococcus equi infection in horses,” Veterinary Microbiology, vol. 14, no. 3, pp. 211–214, 1987.

W. G. Meijer and J. F. Prescott, “Rhodococcus equi,” Veterinary Research, vol. 35, no. 4, pp. 383–396, 2004.

H. Magnusson, “Spezifische Infektioese Pneumonie beim Fohlen. Ein neuer Eitererreger beim Pferde,” Archiv fur Wissenschaftliche und Praktische Tierheilkunde, vol. 50, pp. 22–38, 1923.

J. B. Woolcock, M. D. Mutimer, and A. M. T. Farmer, “Epidemiology of Corynebacterium equi in horses,” Research in Veterinary Science, vol. 28, no. 1, pp. 87–90, 1980.

G. Muscatello, “Rhodococcus equi pneumonia in the foal. Part 1: pathogenesis and epidemiology,” Veterinary Journal, vol. 192, no. 1, pp. 20–26, 2012.

S. Takai, “Epidemiology of Rhodococcus equi infections: a review,” Veterinary Microbiology, vol. 56, no. 3-4, pp. 167–176, 1997.

R. J. Martens, S. Takai, N. D. Cohen, M. K. Chaffin, H. Liu, and S. Lingsweiler, “Prevalence and virulence of Rhodococcus equi in sick foals and soil of horse-breeding farms in Texas,” in Proceedings of the 45th Annual Convention of the American Association of Equine Practitioners (AAEP), vol. 45, pp. 53–55, 1999.

S. Giguere, “Update on R. equi infections in foals,” in Proceedings of the 11th Congress on Equine Medicine and Surgery, pp. 136–141, Geneva, Switzerland, 2009.

D. M. Ainsworth, S. W. Eicker, A. E. Yeagar et al., “Associations between physical examination, laboratory, and radiographic findings and outcome and subsequent racing performance of foals with Rhodococcus equi infection: 115 cases (1984–1992),” Journal of the American Veterinary Medical Association, vol. 213, no. 4, pp. 510–515, 1998.

C. W. Kohn, D. Knight, W. Hueston, R. Jacobs, and S. M. Reed, “Colostral and serum IgG, IgA, and IgM concentrations in Standardbred mares and their foals at parturition,” Journal of the American Veterinary Medical Association, vol. 195, no. 1, pp. 64–68, 1989.

J. R. Hurley and A. P. Begg, “Failure of hyperimmune plasma to prevent pneumonia caused by Rhodococcus equi in foals,” Australian Veterinary Journal, vol. 72, no. 11, pp. 418–420, 1995.

S. Giguère, J. M. Gaskin, C. Miller, and J. L. Bowman, “Evaluation of a commercially available hyperimmune plasma product for prevention of naturally acquired pneumonia caused by Rhodococcus equi in foals,” Journal of the American Veterinary Medical Association, vol. 220, no. 1, pp. 59–63, 2002.

S. S. Caston, S. R. McClure, R. J. Martens et al., “Effect of hyperimmune plasma on the severity of pneumonia caused by Rhodococcus equi in experimentally infected foals,” Veterinary Therapeutics, vol. 7, no. 4, pp. 361–375, 2006.

T. Becú, G. Polledo, and J. M. Gaskin, “Immunoprophylaxis of Rhodococcus equi pneumonia in foals,” Veterinary Microbiology, vol. 56, no. 3-4, pp. 193–204, 1997.

J. E. Butler, “Immunoglobulin diversity, B-cell and antibody repertoire development in large farm animals,” OIE Revue Scientifique et Technique, vol. 17, no. 1, pp. 43–70, 1998.

J. Cauchard, C. Sevin, J.-J. Ballet, and S. Taouji, “Foal IgG and opsonizing anti-Rhodococcus equi antibodies after immunization of pregnant mares with a protective VapA candidate vaccine,” Veterinary Microbiology, vol. 104, no. 1-2, pp. 73–81, 2004.

G. Muscatello, “Rhodococcus equi pneumonia in the foal. Part 2: diagnostics, treatment and disease management,” Veterinary Journal, vol. 192, no. 1, pp. 27–33, 2012.

H. A. Gans, A. M. Arvin, J. Galinus, L. Logan, R. Dehovitz, and Y. Maldonado, “Deficiency of the humoral immune response to measles vaccine in infants immunized at age 6 months,” Journal of the American Medical Association, vol. 280, no. 6, pp. 527–532, 1998.

H. A. Gans, Y. Maldonado, L. L. Yasukawa et al., “IL-12, IFN-γ, and T cell proliferation to measles in immunized infants,” Journal of Immunology, vol. 162, no. 9, pp. 5569–5575, 1999.

K. E. Hooper-Mcgrevy, B. N. Wilkie, and J. F. Prescott, “Virulence-associated protein-specific serum immunoglobulin G-isotype expression in young foals protected against Rhodococcus equi pneumonia by oral immunization with virulent R. equi,” Vaccine, vol. 23, no. 50, pp. 5760–5767, 2005.

R. van der Geize, A. W. F. Grommen, G. I. Hessels, A. A. C. Jacobs, and L. Dijkhuizen, “The steroid catabolic pathway of the intracellular pathogen Rhodococcus equi is important for pathogenesis and a target for vaccine development,” PLoS Pathogens, vol. 7, no. 8, Article ID e1002181, 2011.

S. Takai, S. Kawazu, and S. Tsubaki, “Enzyme-linked immunosorbent assay for diagnosis of Corynebacterium (Rhodococcus) equi infection in foals,” American Journal of Veterinary Research, vol. 46, no. 10, pp. 2166–2170, 1985.

O. Erganiş and E. İstanbulluoğlu, İmmünoloji, Mimoza Basım Yayım A.Ş. Yayın, Konya, Turkey, 1993.

G. C. Hovard and M. R. Kaser, Making and Using Antibodies: A Practical Handbook, CRC Pres Taylor & Francis Group, Boca Raton, Fla, USA, 2007.

A. M. Lopez, H. G. G. Townsend, A. L. Allen, and M. K. Hondalus, “Safety and immunogenicity of a live-attenuated auxotrophic candidate vaccine against the intracellular pathogen Rhodococcus equi,” Vaccine, vol. 26, no. 7, pp. 998–1009, 2008.

T. Phumoonna, Further development of vaccines and diagnostic tests for Rhodococcus equi infection in foals [Ph.D. thesis], Charles Sturt University, Bathurst, Australia, 2005.

R. A. Mansmann and H. D. Knight, “Transtracheal aspiration in the horse,” Journal of the American Veterinary Medical Association, vol. 160, no. 11, pp. 1527–1529, 1972.

T. Higuchi, S. Hashikura, C. Gojo et al., “Clinical evaluation of the serodiagnostic value of enzymelinked immunosorbent assay for Rhodococcus equi infection in foals,” Equine Veterinary Journal, vol. 29, no. 4, pp. 274–278, 1997.

L. G. Luna, Manuals of Histologic Staining Methods of the Armed Forces Institute of Pathology, McGraw-Hill Book Company, New York, NY, USA, 1968.

R. B. Brandon, R. Hill, and R. P. Wilson, “Development of hyperimmune equine plasma to virulence associated protein A (VapA) of Rhodococcus equi,” Plasvacc White Paper, 2009.

S. A. Hines, S. T. Kanaly, B. A. Byrne, and G. H. Palmer, “Immunity to Rhodococcus equi,” Veterinary Microbiology, vol. 56, no. 3-4, pp. 177–185, 1997.

S. K. Hietala, A. A. Ardans, and A. Sansome, “Detection of Corynebacterium equi-specific antibody in horses by enzyme-linked immunosorbent assay,” American Journal of Veterinary Research, vol. 46, no. 1, pp. 13–15, 1985.

J. Cauchard, S. Taouji, C. Sevin et al., “Immunogenicity of synthetic Rhodococcus equi virulence-associated protein peptides in neonate foals,” International Journal of Medical Microbiology, vol. 296, no. 6, pp. 389–396, 2006.

R. J. Martens, J. G. Martens, and R. A. Fiske, “Failure of passive immunisation by colostrum from immunised mares to protect foals against Rhodococcus equi pneumonia,” Equine Veterinary Journal, vol. 23, pp. 19–22, 1991.

J. E. Madigan, S. Hietala, and N. Muller, “Protection against naturally acquired Rhodococcus equi pneumonia in foals by administration of hyperimmune plasma,” Journal of Reproduction and Fertility, vol. 44, pp. 571–578, 1991.

J. Varga, L. Fodor, M. Rusvai, I. Soós, and L. Makrai, “Prevention of Rhodococcus equi pneumonia of foals using two different inactivated vaccines,” Veterinary Microbiology, vol. 56, no. 3-4, pp. 205–212, 1997.

R. J. Martens, J. G. Martens, R. A. Fiske, and S. K. Hietala, “Rhodococcus equi foal pneumonia: protective effects of immune plasma in experimentally infected foals,” Equine Veterinary Journal, vol. 21, no. 4, pp. 249–255, 1989.

T. Higuchi, T. Arakawa, S. Hashikura, T. Inui, H. Senba, and S. Takai, “Effect of prophylactic administration of hyperimmune plasma to prevent Rhodococcus equi infection on foals from endemically affected farms,” Journal of Veterinary Medicine B, vol. 46, no. 9, pp. 641–648, 1999.

S. S. Caston, S. R. McClure, R. J. Martens et al., “Epidemiology and prevention of R. equi pneumonia,” in Proceedings of the 10th International Congress of World Equine Veterinary Association, pp. 343–346, Moscow, Russia, 2008.

G. Perkins, A. Yeager, H. N. Erb, D. Nydam, T. Divers, and J. Bowman, “Survival of foals with experimentally induced Rhodococcus equi infection given either hyperimmune plasma containing R. equi antibody or normal equine plasma,” Veterinary Therapeutics, vol. 3, no. 3, pp. 334–346, 2002.

S. Demmers, A. Johannisson, G. Gröndahl, and M. Jensen-Waern, “Neutrophil functions and serum IgG in growing foals,” Equine Veterinary Journal, vol. 33, no. 7, pp. 676–680, 2001.

C. McTaggart, J. V. Yovich, J. Penhale, and S. L. Raidal, “A comparison of foal and adult horse neutrophil function using flow cytometric techniques,” Research in Veterinary Science, vol. 71, no. 1, pp. 73–79, 2001.

G. Gröndahl, S. Sternberg, M. Jensen-Waern, and A. Johannisson, “Opsonic capacity of foal serum for the two neonatal pathogens Escherichia coli and Actinobacillus equuli,” Equine Veterinary Journal, vol. 33, no. 7, pp. 670–675, 2001.

K. E. Hooper-McGrevy, S. Giguere, B. N. Wilkie, and J. F. Prescott, “Evaluation of equine immunoglobulin specific for Rhodococcus equi virulence-associated proteins A and C for use in protecting foals against Rhodococcus equi-induced pneumonia,” American Journal of Veterinary Research, vol. 62, no. 8, pp. 1307–1313, 2001.

T. R. M. Y. Dawson, D. W. Horohov, W. G. Meijer, and G. Muscatello, “Current understanding of the equine immune response to Rhodococcus equi. An immunological review of R. equi pneumonia,” Veterinary Immunology and Immunopathology, vol. 135, no. 1-2, pp. 1–11, 2010.

T. R. Mosmann and R. L. Coffman, “TH1 and TH2 cells: different patterns of lymphokine secretion lead to different functional properties,” Annual Review of Immunology, vol. 7, pp. 145–173, 1989.

C. C. Breathnach, T. Sturgill-Wright, J. L. Stiltner, A. A. Adams, D. P. Lunn, and D. W. Horohov, “Foals are interferon gamma-deficient at birth,” Veterinary Immunology and Immunopathology, vol. 112, no. 3-4, pp. 199–209, 2006.

C. Ryan, S. Giguère, J. Hagen, C. Hartnett, and A. E. Kalyuzhny, “Effect of age and mitogen on the frequency of interleukin-4 and interferon gamma secreting cells in foals and adult horses as assessed by an equine-specific ELISPOT assay,” Veterinary Immunology and Immunopathology, vol. 133, no. 1, pp. 66–71, 2010.

Anonymous, 2011, http://www.thoroughbredtimes.com/horse-health/2011/01/27/candidate-vaccine-against-rhodococcus-equi-infections-to-be-investigated.aspx